Upload
westernsydney
View
0
Download
0
Embed Size (px)
Citation preview
www.bba-direct.com
Biochimica et Biophysica Acta 1641 (2003) 121–135
Review
Revisiting the role of SNAREs in exocytosis and membrane fusion
Joseph A. Szule, Jens R. Coorssen*
Cellular and Molecular Neurobiology Research Group, Department of Physiology and Biophysics, Faculty of Medicine, University of Calgary,
Calgary, Alberta, Canada T2N 4N1
Received 8 November 2002; accepted 2 May 2003
Abstract
For over a decade SNARE hypotheses have been proposed to explain the mechanism of membrane fusion, yet the field still lacks
sufficient evidence to conclusively identify the minimal components of native fusion. Consequently, debate concerning the postulated role(s)
of SNAREs in membrane fusion continues. The focus of this review is to revisit original literature with a current perspective. Our analysis
begins with the earliest studies of clostridial toxins, leading to various cellular and molecular approaches that have been used to test for the
roles of SNAREs in exocytosis. We place much emphasis on distinguishing between specific effects on membrane fusion and effects on other
critical steps in exocytosis. Although many systems can be used to study exocytosis, few permit selective access to specific steps in the
pathway, such as membrane fusion. Thus, while SNARE proteins are essential to the physiology of exocytosis, assay limitations often
prevent definitive conclusions concerning the molecular mechanism of membrane fusion. In all, the SNAREs are more likely to function
upstream as modulators or priming factors of fusion.
D 2003 Elsevier B.V. All rights reserved.
Keywords: Secretion; Exocytosis; Clostridial toxin; Lipid; Fusion pore; Molecular mechanism
1. Introduction Compartmentalization and the necessity of (regulated)
‘‘It is suggested that in BoTx poisoning the mechanism for
transmitter release has a reduced sensitivity to Ca, and
the level for activation by intracellular Ca is eleva-
ted. . .the release mechanism is in principle intact. . .’’Cull-Candy, Lundh and Thesleff (1976)
Although among the most fundamental and essential of
biological mechanisms, the molecular process of membrane
fusion, in both constitutive and triggered (regulated) release
events, still eludes our extensive attempts to dissect and
understand its underlying progression that results in the
merger of two separate and distinct biological membranes
and the compartments they previously delimited. This effi-
cient, targeted process constitutes the defining step in mech-
anisms as seemingly disparate as neurotransmission, wound
repair, hormone release, fertilization and blood coagulation.
However, might these release events perhaps be more similar
than they initially appear?
0167-4889/03/$ - see front matter D 2003 Elsevier B.V. All rights reserved.
doi:10.1016/S0167-4889(03)00095-8
* Corresponding author. Tel.: +1-403-220-2422.
E-mail address: [email protected] (J.R. Coorssen).
fusion has been a conserved theme in biology. Considering
the extreme energy barriers inherent to the merger of two
distinct membranes, and the molecular rearrangements nec-
essary to accomplish leak-free coalescence of the apposed
membranes into a single continuous bilayer structure [1–5],
it is likely that fusion is a fundamentally conserved cellular
mechanism, and there is evidence to support this concept [6–
11]. It might be supposed that there had even been some
evolutionary processing in this regard, with different molec-
ular steps being optimized by selection until an energetically
efficient series of reactions was available. Subsequent cell
specialization would account for current differences in the
Ca2 + sensitivity and speed of various systems; testing and
selecting alternate Ca2 + sensors (different proteins and/or
isoforms of a given protein) and assorted accessory proteins
resulted in optimized functions in different cell types. The
resulting ‘variations on a theme’ likely consist of the same,
fundamentally conserved fusion mechanism [6–11] elabo-
rated upon with different accessory and modulatory compo-
nents to enhance efficiency, sensitivity to specific triggers
and localization to optimized membrane domains.
Although we take a reductionist approach in our ongoing
research directed toward dissecting the mechanisms under-
J.A. Szule, J.R. Coorssen / Biochimica et Biophysica Acta 1641 (2003) 121–135122
lying the Ca2 +-triggered membrane fusion step(s) of exo-
cytosis, we consider this from an inclusionist point of view;
work from a range of model systems (from yeast-to-inver-
tebrates-to-the-mammalian-CNS) contributes to the under-
standing of fundamental molecular processes. For example,
let us consider the role of ATP. Across several cell types, the
fusion step(s) of exocytosis has been shown to be indepen-
dent of ATP. In 1975, the ATP independence of Ca2 +-
triggered membrane fusion (of fully release-ready vesicles)
was first demonstrated in membrane preparations from
sea urchin eggs [12]. Subsequently, Baker and Whitaker
[13] extended this finding in experiments designed to
characterize the release mechanism. Elegant work from
others [14], studying regulated exocytosis in paramecium,
established that ATP was necessary for maintenance of a
primed release state. Holz et al. [15] confirmed these
findings in neuroendocrine cells, and identified an upstream
ATP-dependent priming stage; a neuroendocrine cell line
was used to identify priming factors [16,17]. The neuroen-
docrine cell studies also identified the rapid depriming of
vesicles (within 2–4 min) that occurs in such cell types
upon the depletion of ATP [15]. Time-resolved assays have
built on these findings to show that only a subpopulation of
morphologically docked vesicles are fully primed and
release-ready [18–20]. The ATP independence of synaptic
vesicle fusion has since been confirmed by Heidelberger et
al. [21]. Thus, before the originally proposed SNARE
hypothesis (suggesting that NSF-induced ATP hydrolysis
disrupts an inter-membrane complex and thereby induces
fusion [22,23]), it was known that ATP was required for
exocytosis, but not for the membrane fusion step(s).
As every system and every research approach has its own
inherent strengths and weaknesses as a ‘tool,’ we have tried
to refine our functional assays, indeed our interpretations, to
focus on the Ca2 +-triggered steps of membrane fusion. This
is particularly relevant to the current review in that much of
exocytosis research deals with ‘readouts’ of fusion rather
than direct measurements of the fusion step(s) itself. Caveats
to consider include (i) that we do not know all molecular
components, steps or events in the pathways of exocytosis
or fusion; and (ii) that most assays assess the pathway as a
whole or at best multiple molecular steps underlying a part
of the pathway. Thus, in our own work, we have found it
necessary to use a specific terminology in reference to
different pre-fusion, triggering and fusion events. We em-
ploy this terminology as an additional tool, to avoid seman-
tic and thus interpretational ambiguities; similar definitions
are broadly accepted in the field [24]. Thus, we define
membrane fusion as the full, non-leaky merger of two
previously distinct bilayer membranes into one continuous
bilayer via a ‘fusion pore;’ hemifusion refers to the merger
of only the proximal monolayers of two apposed bilayer
membranes. By extension, we consider the ‘fusogen,’ or the
‘fusion machine,’ to be that molecular entity directly re-
sponsible for the membrane merger event itself. By defini-
tion, all other molecular components and steps are
supportive or modulatory relative to the function of this
molecular entity. We also consider ‘pore expansion’ to be a
separate stage based on the existence of transient (‘kiss-and-
run’) fusion events [25–27] and evidence for specific
modulation of the expansion process [28–30]. Accordingly,
vesicle content extrusion after fusion may be yet another
mechanistically separable stage [31] or a simple physical
consequence of pore expansion and full (irreversible) merg-
er of the two fusing membranes.
Endocytosis, a multi-step fission process that recycles
membrane from the plasma membrane (PM), is the next
stage in the cyclic exocytotic pathway, but beyond the scope
of this review. In very general terms, endocytotic vesicles
pass either through the lysosomal system or rapidly re-enter
the small pool of actively recycling vesicles (f 10% of the
total vesicle population in a presynaptic bouton) [32,33].
Vesicles in the cytosol appear to exist in one or more
‘reserve’ populations that can be recruited to PM release
sites as required. Such vesicles must be appropriately
targeted and transported to sites on the PM. Although
possibly inter-related, we currently consider transport and
targeting to be effected by distinct, separable mechanisms.
Indeed, there appears to be much overlap of the subsequent
(or parallel) pre-fusion mechanisms that are broadly defined
as tethering, priming and docking. For the purposes of
working definitions, we describe tethering as an initial
stabilized contact between the vesicle and a targeted site
on the PM; this is a developing research focus [34,35].
Although likely to be multi-step processes with substantial
molecular and temporal overlap, we define priming and
docking as a potentially separable series of events. Here,
priming refers to any molecular reaction(s) that contributes
to optimization of the fusogenic potential of the vesicle, and
to its fully docked state; effective docking is required for the
most efficient translation of subsequent signals (‘triggers’)
for the fusion of the apposed vesicle and PM. As will be
described, SNARE interactions may thus be key (perhaps
culminating) events in priming. We consider ‘docked’ to be
the most fully optimized stage of inter-membrane contact
that can exist prior to actual fusion, and such vesicles
(forming only a very small proportion of vesicles that
appear morphologically attached to the PM) are often said
to be immediately ‘release-ready,’ awaiting only the neces-
sary trigger to initiate fusion (an appropriate increase in the
local [Ca2 +]free in many instances) [18,20,36]; we do not, at
the moment, subscribe to the idea that this represents a
hemi-fused state per se [37], but recognize that rapidly
passing through such a localized conformation is likely a
requisite molecular rearrangement on the molecular path-
way to fusion [38–40].
We stress that the actual molecular components essen-
tial (necessary and sufficient) to the stages described above
are as yet largely unknown, or at least unverified in terms
of definitive (but perhaps overlapping) roles in specific
steps of the overall exocytotic pathway. Indeed, at the
molecular level, many of these stages, particularly priming,
J.A. Szule, J.R. Coorssen / Biochimica et Biophysica Acta 1641 (2003) 121–135 123
docking, triggering and fusion, may well be rapid, tran-
sient, multi-step processes that are not easily dissected
experimentally. This emphasizes the fact that many estab-
lished assays actually assess multiple stages of the exocy-
totic pathway, and it is thus often impractical to claim
direct measure of fusion when either (i) changes in the
release of vesicular content are detected from (semi)intact
preparations; (ii) other stages in the pathway cannot be
directly and independently assessed; or (iii) the membranes
undergoing fusion cannot be directly verified. If interven-
tion does not change the assay outcome, fusion is unlikely
to have been affected, but if exocytosis is altered, this is
not evidence for a direct effect on the fusion step(s)
themselves.
2. An early tool: clostridial toxins
The clostridial neurotoxins have been among the most
important tools in understanding the exocytotic pathway.
Originally thought only to block neuronal function, this
selectivity of binding and uptake was eventually shown to
reside with the heavy chains of these toxins, while the
catalytic light chains (Zn2 +-dependent metalloproteinases)
are the actual active components that effect blockade of
neurotransmitter exocytosis [41]. This distinction led to
identification of the putatively selective substrates of these
toxins, the SNARE proteins [42,43]. Many VAMP/synapto-
brevin isoforms are cleaved by tetanus toxin (TeTx) and
botulinum toxin (BoTx) B, D, F and G, SNAP-25 isoforms
by BoTx A, C and E, and Syntaxins by BoTx C (reviewed
in Refs. [41,44]). Notably, mutations have resulted in at
least one cleavage resistant native isoform of each of the
three SNARE proteins (reviewed in Ref. [44]).
For well over a century, medical science has sought to
understand the actions of the clostridial neurotoxins. Many
of these now classical works highlight initial studies into
synaptic mechanisms and the vesicular hypothesis of neu-
rotransmission, thus charting the course of modern neuro-
physiology. Considering that the molecular targets and even
the proteolytic nature of the clostridial neurotoxins were
unknown at the time, these studies were elegantly insight-
ful. As early as 1939, Harvey [45] noted that spontaneous
release (muscle activity) still occurred following poisoning
with TeTx, and that repetitive stimulation (even by only
two effectively spaced stimuli) resulted in increased activ-
ity; increased intra-terminal [Ca2 +]free overcame the block
by TeTx. These findings were confirmed for preparations
poisoned with BoTxA [46], in which depolarization with
KCl was also shown to produce a transient recovery. The
work of Burgen et al. [46] was also important for extending
substantially earlier original observations that decreased
activity (of the test subject/preparation and thus of synaptic
activity) would slow the rate and extent of poisoning. These
observations suggest that synaptic activity (turnover in the
cyclic exocytotic pathway) enhances the effect of the toxins
and that the block must lie upstream of the fusion reaction
since enhanced stimulation can elicit some release (fusion),
albeit from a now rapidly exhaustible pool [47] (see also
Ref. [48]). Brooks [49,50] soon after concluded that
BoTxA did not directly inactivate the release mechanism
itself. Thesleff [51] also noted that doubling the external
(bath) [Ca2 +], adding TEA or inducing mechanical injury
to the motor-endplate overcame the block of release by
BoTx A. Spontaneous release events in denervated nerves
were also much less sensitive to BoTxA, again suggesting
that synaptic activity (vesicular turnover) promoted the
ability of the toxin to affect a block of neurotransmission
(see also Ref. [47]). Tetanic stimulation and reduced
temperatures were also shown to overcome blocks by both
BoTx A and TeTx [52].
Extensive studies by Parsons et al. [53], and by Harris
and Miledi [54], confirmed many of the findings described
above, illustrating [Ca2 +]-dependent recovery from TeTx
and BoTxD intoxication, respectively, by increased exter-
nal [Ca2 +], KCl-depolarization and paired stimuli. Both
studies reached conclusions of substantial long-term im-
portance to understanding synaptic function: toxin (i)
decreases the probability of transmitter release [53]; and
(ii) interferes with stimulus-secretion coupling [54,55].
More recent work on factors affecting SNARE complexes
has now reached similar conclusions regarding effects on
release probability [56,57], but the underlying mechanism
remains unknown. Notably, repetitive stimulation was also
shown to transiently relieve a complete block of neuro-
transmission produced by TeTx [58]. The most extensive
single analysis (even including a second dose of toxin)
may well be that by Cull-Candy et al. [59], who concluded
that the block by BoTxA affected the Ca2 + sensitivity of
the release mechanisms while clearly leaving the actual
fusion machinery intact. Thus, several decades of work
indicated that the target(s) of the clostridial neurotoxins
(then unknown) are not minimal essential components of
the native fusion machine, but rather that they are impor-
tant upstream modulators of synaptic efficacy. Subsequent
elegant studies also demonstrated distinct pre-fusion sites
of action of the different clostridial toxins, including effects
on priming [52,60–64]. However, caveats to be considered
include (i) the effectiveness and purity of some of the early
toxin isolates; (ii) the possibility that some nerve fibres
escape poisoning in the tissue preparations used; and (iii)
the potential presence of toxin-insensitive SNARE iso-
forms that might still function in a manner consistent with
the SNARE hypothesis. The first and second issues are
well addressed by the general consistency of findings,
using a variety of toxin and tissue preparations over several
decades, and by the range of toxin doses and poisoning
periods studied over this time. In addition, Cull-Candy et
al. [59] used second applications of toxin to ensure full
extent of poisoning. Gansel et al. [60] also used toxin
combinations, all without additional effect. However, the
potential presence of low levels of compensatory, toxin-
J.A. Szule, J.R. Coorssen / Biochimica et Biophysica Acta 1641 (2003) 121–135124
insensitive SNAREs cannot be easily ruled out in these or
other studies, yet recovery after extensive, long-term
blockade of exocytosis only occurs via the sprouting of
new terminals.
3. Comparative studies of toxin action
Despite the availability of the clostridial toxin light
chains, several factors have hampered the usefulness of
these toxins in terms of clearly defining the role(s) of the
SNARE proteins. These problems include the (i) existence
of toxin-insensitive SNARE isoforms, and (ii) lack of
routine, highly sensitive quantitative assays (to confirm
the extent of SNARE cleavage). These issues are further
complicated by the lack of selectivity of most assay systems
for specific steps in the exocytotic pathway; an observed
effect of these toxins in a given cell type clearly indicates a
role for the SNAREs in the dynamics of the cyclic exocy-
totic pathway, but tends to provide little additional evidence
as to the actual molecular contribution(s) of these proteins to
membrane fusion. While such experiments have been car-
ried out in a wide range of different constitutive and
regulated secretory cell types, blockade of release is rarely
consistent or complete [52,59,60,63–71]. While these stud-
ies clearly indicate strong evolutionary conservation of
molecular mechanisms involving SNAREs at one or more
stages of the exocytotic pathway, more definitive conclu-
sions are difficult. However, the ability to bypass clostridial
blockade clearly demonstrated that fusion mechanisms
remained intact and functional. Ca2 +- but not GTPgS-
triggered insulin release was blocked by TeTx and BoTx
B [72]. The BoTx A and C block of neurotransmission in
cultured hippocampal neurons could be partially overcome
by increased intra-terminal [Ca2 +]free, addition of cAMP or
by substituting Sr2 + for Ca2 + [68]. Fassio et al. [73] showed
that increased [Ca2 +]free (via ionophore) could bypass
inhibition of exocytosis by TeTx and BoTx F. Similar to
the early work on the neuromuscular junction, these studies
indicate that the final membrane fusion steps of excocytosis
are still functional after selective SNARE cleavage by the
different clostridial toxins, but that upstream regulation by
Ca2 + is perturbed. This conclusion is substantiated by work
in three very different systems.
First, despite extensive treatment with clostridial toxins
(singly or in combination) effecting the removal of the bulk
of the resident SNARE proteins from fully Ca2 + sensitive,
fusion-ready cortical vesicles (CV) isolated from unfertil-
ized sea urchin eggs [36,74,75], there was no effect on
Ca2 +-triggered homotypic fusion [76,77]. These findings
(1997–1998) were confirmed and extended using a variety
of coupled functional and biochemical assays, leading to the
conclusion that the SNARE complex might promote the
Ca2 + sensitivity of late triggered steps of exocytosis, but
was not an essential component of the minimal native fusion
machine [36,75–77]. Notably, fusion in the intact urchin
egg can be disrupted by clostridial toxins if the eggs are first
treated so as to un-dock CV from the PM, implying a more
likely role for the SNAREs in targeting and docking [78].
Second, studies focussing on the homotypic fusion of
isolated yeast vacuoles also indicated that SNAREs func-
tioned upstream of fusion; trans SNARE complexes
appeared to ‘activate’ a pathway to fusion, but the presence
of these complexes was not required for subsequent prog-
ress through the fusion pathway [79–82].
Third, detailed time-resolved analyses of Ca2 +-triggered
exocytosis from bovine chromaffin cells treated with differ-
ent clostridial toxins indicated inhibition of both the fast and
slow phases of exocytosis; BoTx A had the weakest effect
[70]. Inhibition of the slower phases of exocytosis implies
blockade of one or more steps upstream of fusion. Attempts
to use higher [Ca2 +]free to bypass the clostridial block were
confounded by a large release response that did not correlate
to dense core vesicles; elevated [Ca2 +]free are known to
trigger exocytosis of lysosomes in many cell types [83,84].
Nevertheless, there are several points to be considered in
interpreting these experiments. An ultra-fast phase of vesicle
release appeared still to be present in the toxin-treated cells;
the change in membrane capacitance upon triggering was
still equivalent to that measured for a small pool (f 10–35)
of fully release-ready vesicles [85–89]. A corresponding
amperometric signal appeared in some experiments but not
all [70]. The presence of this pool is somewhat surprising.
This small pool is most easily interpreted to represent fully
docked and release-ready vesicles, presumably with
SNARE proteins already complexed and thus inaccessible
to the clostridial toxins. However, observations of vesicle
dynamics near the PM indicate that even attached (‘docked’)
vesicles turn over within f 100 s [90]; pre-stimulus incu-
bations were for f 10 min in the experiments with clos-
tridial toxins [70]. If these vesicles were fully docked prior
to toxin delivery through the patch pipette, why did they not
dissociate from the membrane and become toxin sensitive
during the pre-stimulus incubation? If they did, how did
other vesicles, previously exposed to toxin, replace them?
One possible explanation is that many intact SNAREs might
still be operational in these experiments. There are clear
differences in the cleavage susceptibilities of recombinant
SNAREs in vitro and SNAREs in a native membrane. As
current measures of SNARE density on secretory vesicles
are f 10 times higher than estimated for the in vitro tests
used to assess toxin efficiency [70], substantial amounts of
functional SNARE proteins likely remained [91]. Then why
was exocytosis affected in the manner detected? Again, the
results are most simply interpreted to indicate that the
SNAREs function upstream of fusion, promoting the ‘nor-
mal’ physiological response because extensive secretion
was inhibited, but the actual fusion event was not (ultra-
fast phase). Combined with the findings described above,
from the experiments using CV and yeast vacuoles, the
results might be interpreted to indicate that once a group of
vesicles have gone through a trans SNARE ‘priming’ step,
J.A. Szule, J.R. Coorssen / Biochimica et Biophysica Acta 1641 (2003) 121–135 125
they, for some period of time, remain prepared to engage in
rapid fusion, and therefore represent a highly release-ready
pool. In some systems such as neuroendocrine cells, this
dynamic primed and immediate fusion-ready state might last
for f 2–4 min in the presence of cytosol, for up to 90 min
in yeast vacuoles, and for tens of hours (or longer; in the
absence of cytosol) in isolated CV [36,76]. This long-lived
fully primed and fusion competent (stage-specific) state of
docked CV, together with the Ca2 +-triggered disassembly of
SNARE complexes prior to fusion, has led to one possible
interpretation being that the SNAREs have not only carried
out their essential function(s) in exocytosis by this point, but
that their regulated removal from the site of inter-membrane
contact represents a critical step to ensuring fast, efficient
fusion [75].
A second study by Xu et al. [92] used an antibody (Fab
fragment) to SNAP-25, known to block SNARE complex
formation in vitro, to test the role of the complex in the
late Ca2 +-triggered steps of exocytosis. Again, both the
fast and slow phases of release were perturbed, but the
fusion machinery was clearly intact. Slowing the kinetics
of triggered release suggests a modulatory role for the
SNARE complex, consistent with an influence on the
probability of fusion in the physiological range of
[Ca2 +]free. The interpretation was that ‘loose’ inter-mem-
brane SNARE complexes were sufficient to support fusion
but that fully ‘zippered’ complexes were necessary for fast,
triggered fusion; these different states of the SNARE
complex may correlate with previously described differ-
ences in sensitivities to clostridial toxins [48]. However, as
SNARE complex formation in vitro has been suggested to
correlate with cis rather than trans complexes, and native
complexes were not assayed in this study [92], more
definitive statements concerning sites and effects of the
Fab fragment binding cannot be made. As with the earlier
experiments involving clostridial toxins, there is a question
as to why an incomplete block of the burst phase of release
occurs if fully docked vesicles turn over during the 10-min
intracellular exposure to the blocking antibody. Alterna-
tively, one might also postulate that binding of the Fab
fragment prevented effective clearance of SNARE com-
plexes thereby blocking fast, efficient fusion. However,
considering as a whole all the studies described above, and
noting that (i) the extent of inhibition of exocytosis by a
given clostridial toxin varies widely among different cell
types; and (ii) standard Western blotting or immunocyto-
chemical analyses are inherently insensitive, potentially
‘missing’ thousands or more copies of a given protein
(increased risk of ‘false-negative’ results) [91], firm con-
clusions as to the actual function(s) of the SNARE proteins
remained difficult. There was no way of confirming
whether the actual amounts of intact SNARE proteins
remaining after clostridial toxin treatments were sufficient
to account for the remaining function, whether SNARE
fragments acted to promote function [93,94], whether
residual function was due to the presence of toxin-insen-
sitive SNARE isoforms, or some combination of the above.
Additional clostridial toxin targets also could not be ruled
out [95–100].
As an alternative, molecular genetic approaches have
also been applied to the question of SNARE function. While
these studies have taught us a great deal concerning details
of protein–protein interactions, providing tools that will
undoubtedly prove invaluable to future mechanistic studies,
many of the same issues outlined above plague a definitive
interpretation of SNARE functions in membrane fusion.
While various SNARE mutations block or modify exocy-
tosis to varying extents, the assay formats used do not
permit detailed analyses of the Ca2 +-triggered fusion steps
themselves. Early SNARE mutations/knockouts in C. ele-
gans and Drosophila yielded results consistent with the
early clostridial toxin work in neuromuscular junction
preparations; fusion still occurred (spontaneous release),
but regulation of the release process was disrupted [101–
105]. Up-regulation of syntaxin 1A suggests a distinct role
in defining vesicles for the regulated secretory pathway
[106–108], and VAMP mutations suggest disruptions of
vesicle targeting and docking [109]. Washbourne et al. [110]
showed that SNAP-25 mutants incapable of binding VAMP
still support exocytosis. In addition, SNAP-25 mutations
that should disrupt SNARE complex formation and stability
still support normal exocytotic release from neuroendocrine
cells [111]. Most recently, knockouts of neural SNAP-25
[112] and VAMP2 [113] in mice (also showing perturbed
regulation of release) have been suggested to indicate that
SNAREs may not be essential to fusion. However, addi-
tional treatments with clostridial toxins were not performed
[114], and the presence of compensatory SNARE isoforms
cannot be ruled out. The evidence for such potential ‘rescue’
in vivo is clear [115–117]. Therefore, unless all the known
isoforms of a given SNARE in a specific organism can be
simultaneously knocked out, SNARE hypotheses remain
difficult to test even with the power of molecular genetics.
Given the critical role(s) of SNAREs in the exocytotic
pathway, even this approach would not provide a defin-
itive assessment as it would likely be fatal quite early in
development. Inducible knockouts are an obvious alterna-
tive, but still cannot address the issue of multiple SNARE
isoforms.
4. Fusion in vitro
One possible approach to testing SNARE hypotheses
requires the use of a stage-specific preparation such as the
urchin CV; by all available criteria [36,75,118], Ca2 +-trig-
gered CV–CV fusion in vitro, in the absence of cytoplasmic
factors, occurs through the same molecular pathway as
exocytotic release. Since cytoplasmic components, including
SNARE recruitment and assembly factors [119,120], are not
required for triggered CV fusion, an upstream modulatory
role (e.g. pre-fusion) for the SNAREs is suggested. Further-
J.A. Szule, J.R. Coorssen / Biochimica et Biophysica Acta 1641 (2003) 121–135126
more, despite extensive analysis by a number of laborato-
ries, evidence suggests CV membranes contain only one
isoform of each of the SNARE proteins [76,121]. Consid-
ering the sensitivity of both triggered fusion and the SNARE
proteins to proteases such as trypsin, it was anticipated that
treating isolated CV (thus exposing the entire complement
of vesicular membrane proteins) with broad spectrum pro-
teases might produce a ‘biochemical knockout’ of one or
more of the SNARE proteins [36]. If fusion persisted after
such treatments, a direct role for the SNAREs as essential
components of the native fusion machine would be ruled
out. This approach, utilizing stage-specific native mem-
branes, makes no assumptions as to which proteins are
important, and would theoretically result in complete
SNARE removal as all known SNARE isoforms (including
those insensitive to the clostridial toxins) have an exten-
sively conserved number of potential cleavage sites for
proteases such as trypsin. Indeed, the extensive cleavage
of SNAREs in vitro and in vivo has been demonstrated.
However, the effective analysis of a molecular mechanism
requires the accurate identification and quantification of
specific proteins. A quantitative, ultra-sensitive immuno-
blotting protocol has been developed and optimized [91].
Coupling sensitive detection with broad spectrum prote-
ase treatments has now permitted direct testing of SNARE
hypotheses. Quantitative removal of all three types of
SNARE proteins, in some cases including the complete
removal of syntaxin from CV, does not block Ca2 +-trig-
gered fusion [122,123]. Furthermore, despite substantial
ablation of the resident CV SNAREs (zf 90%), clostri-
pain treatments had no effect on the Ca2 + sensitivity or
extent of fusion or, perhaps most importantly, on the kinetics
of fusion. This is perhaps the most direct evidence that
SNAREs are unlikely to be essential components of the
minimal native fusion machine; if essential, such substantial
removal should most certainly have affected the kinetics of
Ca2 +-triggered fusion. Furthermore, the estimated energy
contributed by SNAREs and associated proteins (f 2 kT)
[123] is lower than that thought to be required to overcome
the hydration energy barrier at the membrane surface [124]
or for bilayer merger [3,5,125]. Differential protease effects
suggest the existence of a native fusion machine with an
inherently low Ca2 + sensitivity. One hypothesis is that
SNAREs and their immediate binding partners may act to
modulate the Ca2 + sensitivity of this native machine into the
physiological range of [Ca2 +]free [123].
The simplest interpretation of the above study is that
SNAREs are not essential components of the minimal native
fusion machine; there is little possibility of compensatory
proteins preserving function in the Ca2 +-triggered fusion
pathway of this particular stage-specific system. These find-
ings are consistent with work in the yeast vacuolar system
suggesting the existence of a fusion mechanism functioning
downstream of the SNAREs [81,82]. In addition, mutations
in genes related to fatty acid elongation and sphingolipid
synthesis bypass the need for vesicular SNAREs, suggesting
that SNAREs contribute to docking and the efficiency of
fusion, but not to the fusion mechanism per se [126].
Although not yet verified in other systems, these studies on
CV and yeast vacuoles support the concept of an upstream
‘priming’ role for the SNAREs, with alternate factors under-
lying the actual membrane merger steps. In contrast, other
work on constitutive exocytosis in yeast has led to an
alternate view of SNARE function, suggestive of a role in
fusion. In these studies, SNARE transmembrane regions
were replaced with covalently attached lipid moieties (ger-
anylgeranylated) and the slow constitutive pathway was
blocked; these results have been interpreted to suggest that
the transmembrane domain of SNAREs can function late in
fusion [127], an idea supported by studies demonstrating that
peptides corresponding to these transmembrane regions can
induce fusion of artificial membranes [128]. For reasons that
are not immediately apparent, these results are inconsistent
with the work on yeast vacuole fusion that indicates SNAREs
are not required at the fusion step [81,82]. Overall, both sets
of results in the yeast system appear inconsistent with the fact
that isolated CVand other native vesicles can fuse with pure
lipid target membranes [129–132]. While consistent with a
lipidic fusion pore, these results are more difficult to reconcile
with a proteinaceous, ‘channel-like’ fusion-pore, although
triggered conformational changes of a proteolipid could
perhaps contribute. Furthermore, recognized viral fusogenic
proteins, to which SNAREs have been compared, will also
catalyse merger with protein-free target membranes [133–
135]. This is most interesting when considering the saddle
model of hemagglutinin-induced fusion, where the viral
peptide inserts into its own membrane rather than the target
membrane [136]. SNAREs appear incapable of triggering
comparable events [137].
Thus, although hypotheses concerning transient inter-
membrane ‘‘SNAREpins’’ as fusion complexes are ques-
tionable in light of the results of studies in a number of
model systems, alternate hypotheses concerning the in-
volvement of SNARE transmembrane regions in hemifusion
intermediates require further investigation. However, it
remains unclear how these transmembrane regions would
converge in cases of cytosolic domain disruptions (that
obviate inter-membrane complex formation and function),
or in the absence of additional cytosolic factors that are
suggested to promote complex formation [119,120,138]. If
SNARE clearance from the fusion site is required for fast,
efficient fusion, convergence of these transmembrane
regions seems unlikely unless it contributes to localized
membrane destabilization well before the actual fusion
event, which might be promoted by specific membrane
domains [139].
5. Reconstitution
The strongest case for the SNAREs as fusogens has come
from the work of Weber et al. [137] who have used recom-
J.A. Szule, J.R. Coorssen / Biochimica et Biophysica Acta 1641 (2003) 121–135 127
binant SNAREs reconstituted into artificial lipid membrane
systems to study the effects of SNARE interactions in vitro.
This technically complicated experimental approach has
become an elegantly routine assay system in this group
[137,140–146]. The type of lipid vesicle preparation used
(small unilamellar liposomes) was originally developed to
retain small soluble content markers, the mixing of which
could be used to assess actual fusion events. Simply
assessing intermixing of membrane lipids was unsatisfacto-
ry as it did not represent complete fusion, and could even
occur by transbilayer exchange under conditions of close
inter-membrane apposition. One of the principal concerns
with interpretation of the reconstituted SNARE assays is
that this system has never demonstrated the capacity to
retain low molecular weight solutes; even large (f 5 kDa)
oligonucleotide markers showed a high level of ‘leakage’
[141]. But SNAREs are clearly capable of interacting to
yield complexes that could promote closer apposition of
membranes [147]. Although SNAREs may contribute, in
part, to overcoming the energy barrier imposed by the
ubiquitous hydration layer [1], and thereby perhaps promot-
ing nonspecific lipid exchange between the apposed mem-
branes, this state would be unlikely to spontaneously yield a
fusion site unless the bilayers were already destabilized.
Strong, nonselective increases in inter-membrane attractive
forces in vitro have indeed been shown to sufficiently
reduce inter-bilayer distances such that local dehydration
induces hemifusion [148,149]. It is unclear from the pub-
lished reconstitution assays the extent to which lipid ex-
change and bilayer mixing each contribute to the measured
signals, and to what extent the signals being assessed are
actually comparable to a native fusion event. Lipid bilayer
contact is required for bilayer mixing but not for nonspecific
lipid exchange. The structure of the SNARE complex [147]
suggests that an intervening hydrated interface of f 2nm
must remain between the SNARE-apposed membranes, thus
favouring nonspecific lipid exchange over true bilayer
mixing. This concern is reinforced when SNARE densities
are considered. Recent assessments reveal a striking simi-
larity between the SNARE densities measured on CV and
synaptic vesicle membranes [91]. These native SNARE
densities are 50-fold lower than required in the reconstituted
SNARE preparations [137]. Although a recent report indi-
cates that the in vitro assays will work with lower VAMP
densities, the VAMP was replaced with recombinant syn-
aptotagmin, which does not allay concerns regarding the
bilayer status (stability) of these preparations [142]. Clearly,
such a substantial increase in the local energy contributed by
SNAREs, relative to that in stable native membranes, could
well promote a nonspecific membrane merger event, but this
is unlikely to be representative of a biological fusion site. If
this is indeed what is occurring, it might, in part, explain the
rather slow fusion kinetics in these reconstituted systems
relative to triggered fusion in vivo. Although an increase in
[Ca2 +]free triggers fast fusion events in most secretory cell
types [18,20,150,151], reconstitution of synaptotagmin, the
putative essential Ca2 + sensor for triggered release does not
enhance fusion in the reconstituted preparations [142].
Similarly, lipid mixing between isolated synaptic vesicles
(containing synaptotagmin) and SNARE-containing lipo-
somes can be triggered by aggregation alone and is rela-
tively slow even at high [Ca2 +]free [152].
Over the last several decades, a substantial number of
proteins have been shown to promote aggregation, adhe-
sion, lipid mixing and even fusion in model membrane
systems [149,153–163]. In many cases, this fusion also
involves content mixing, is reasonably fast, and can be
triggered in some fashion that is at least reminiscent of
biological fusion events. Thus, there are clearly differences
between what can be demonstrated in vitro and actual
protein functions in vivo [164]. Although the native
cellular localization of the SNAREs may make these more
likely candidates than some of the other proteins shown to
promote fusion in vitro, this does not constitute evidence
that the results of assays in the reconstituted SNARE
preparations actually describe a minimal biological fusion
machine. Thus, although it has been argued that additional
factors may be present in native systems and that these
promote SNARE function, this is one possible interpreta-
tion, and not evidence supporting a role for the SNARE
complex as the minimal fusogenic entity. Indeed, the
SNARE interacting protein N-ethylmaleimide (NEM)-sen-
sitive factor (NSF), which is thought to mediate post-
fusion uncoupling of SNARE complexes and thus promote
their functions in vivo, has also been shown to indepen-
dently promote the fusion of liposomes [161,162,165]. It
has been argued that this effect of NSF is limited to
liposomes of specific lipid composition, and that since the
effect of the SNAREs extends to other lipid mixtures, the
SNARE complex represents a minimal fusogen [163].
However, liposomes are rarely used in an effort to mimic
global lipid compositions of entire cellular systems; rather,
they are most often used to mimic localized sites on
membranes. If a proteinaceous fusion machine (SNARE or
otherwise) has been evolutionarily conserved and opti-
mized, it seems unlikely that the same rationale does not
apply to the lipid components that form the bulk of the
membrane, and are the local substrates on/with which the
proteins must function. To postulate that one lipid mixture
is more likely or appropriate than another implies knowl-
edge of the actual lipidic species functioning at the native
fusion site. To the best of our knowledge, such specifics
remain unknown, although much elegant work has sug-
gested that certain lipid species are more likely than others
[129,131,132,159,165,166]. If optimization of the focal
lipid mixture at the fusion site is not critical, then SNARE
complexes at native densities [91] should also drive the full
fusion of membranes composed primarily of saturated, long
chain species of phosphatidylcholine, sphingomyelin or
ceramide; we are unaware of such a study. However, as
isolated CV are at a stage of fusion readiness that no longer
requires cytosolic factors, we suggest that NSF and other
J.A. Szule, J.R. Coorssen / Biochimica et Biophysica Acta 1641 (2003) 121–135128
identified promoters of SNARE function [119,120,167] are
more likely to act upstream of the triggered native fusion
event, and possibly also in later modulatory roles [168].
Thus, the reconstituted systems have demonstrated that the
SNAREs may code for some level of selectivity in regulating
the interactions of specific intracellular compartments
[169,170], and that the resulting inter-membrane complexes
may contribute to defining potential fusion sites. Therefore,
roles in targeting, docking and priming steps of exocytosis
are possible (e.g. pre-fusion), and disruptions at one or more
of these stages could explain the altered functions observed
when the cellular complement of SNAREs is targeted by
toxins, peptides, and so forth [59,70,92,171,172].
6. Biophysics of membrane fusion
Bilayer membrane fusion has been described in terms of
a progression of intermediate structures of lower free-
energy, which involve rearrangements of the lipid matrix.
Detailed mathematical modeling has been used to explore a
number of potential molecular-structural models; the se-
quence of structural rearrangements corresponding to the
lowest-free energy states has been identified as that involv-
ing a ‘stalk-pore’ transition [3,40,125,173,174]. The initial
step in this sequential rearrangement and merger of focally
apposed bilayer domains requires an input of energy to
overcome the hydration and molecular repulsive barriers
[1,2,175], thus bringing the apposed membranes into mo-
lecular contact. The subsequent rearrangements of the lipid
matrix reduce the net free-energy of the lipid assemblies,
mainly through the reduction of interstitial and curvature
energies. Interstitial energy can be reduced by hydrophobic
molecules occupying the interstitial volumes (within the
hydrophobic domain of the membrane) [176–179], or by
alternate packing and tilt of the acyl chains [5]. Curvature
energy is described in terms of spontaneous curvature,
where the curvature of a monolayer minimizes the bending
elastic free-energy [176]. Various lipid species influence the
spontaneous curvature of a membrane, either by adding
zero curvature energy, positive curvature energy (increased
propensity to forming curved assemblies with the polar
groups on the convex side) or negative curvature energy
(increased propensity to forming curved structures with
the polar groups on the concave side) [180]. Therefore,
the curvature properties of the lipids that compose fuso-
genic membranes influence the transition of intermediate
structures [39,181].
Briefly, the proximal (contacting) monolayers of the
apposed bilayer membranes merge, forming a contiguous,
highly curved ‘hourglass’ structure with a net negative
curvature (polar groups on the concave side), sandwiched
between the still intact distal (non-contacting) monolayers of
the apposed membranes (see Fig. 1 of Ref. [3], or Fig. 4 of
Ref. [181]); the result is an inter-membrane ‘stalk,’ which
defines a hemifusion state. Once formed, the stalk expands,
thinning until the distal monolayers merge, forming a lipidic
fusion pore which has a net positive curvature (polar groups
on the convex side). Recently, it was demonstrated that
model lipid assemblies undergo fusion through a process
that is consistent with stalk formation [182], and this has also
been seen in molecular dynamic simulations [183]. Exis-
tence of a stalk-like intermediate in native membrane fusion
is supported by the reversible block of a range of biological
fusion reactions by lysophospholipids [39,184,185]. This
block is downstream of SNARE function, and occurs irre-
spective of SNARE protein complexes functioning upstream
[76]. A lysophosphatidylcholine block was used to show that
SNARE interactions were not strict determinants of a docked
vesicle. SNAREs may function early in tethering/docking,
but their interactions are not essential to maintenance of the
fully docked and release-ready state [75]. Similar conclu-
sions have been reached using total internal reflection
fluorescence microscopy of TeTx and BoTx A expressing
chromaffin cells [186].
7. The Ca2+-triggered fusion steps of exocytosis
A decade of testing SNARE hypotheses has thus far not
provided the definitive experiment(s) to fully assess SNARE
contributions to exocytosis, although work on protease-
treated CV does indicate that SNAREs likely function
upstream of the (regulated) fusion steps [123]. Identification
of the SNAREs and a large number of interacting proteins
has provided a substantial catalogue of components neces-
sary for effective functioning of the exocytotic pathway.
Considering tests of function since the earliest neurophys-
iological analyses of clostridial toxin effects, we have
critically evaluated the most probable role(s) of the
SNAREs in the exocytotic pathway. Despite a range of
hypotheses, we currently view the SNAREs as modulatory
(promoting), working upstream of fusion and not represent-
ing minimal essential components of the native mechanism
directly responsible for the membrane merger events of
exocytotic fusion. Clearly, there are important implications
for current research directions, for mechanistic models of
exocytosis and for a molecular-level understanding of the
(regulated) fusion pathway.
While SNARE modulatory functions are clearly essential
to the physiology of exocytosis, perhaps in part defining
potential native fusion sites, there is clearly a difference
between contributions to the establishment and efficiency of
a mechanism, and the mechanism itself. We interpret the
SNAREs and associated proteins to function in targeting,
docking and priming, perhaps in the last priming step that
ensures full Ca2 + sensitivity, and thus a rapid, triggered
fusion response. Changes induced by SNARE complexation
result in an activated, fusion-ready state, and subsequent
mechanistic steps leading to fusion may well be SNARE-
independent, possibly even requiring disassembly (clear-
ance) of SNARE complexes in order to most fully facilitate
J.A. Szule, J.R. Coorssen / Biochimica et Biophysica Acta 1641 (2003) 121–135 129
the membrane merger steps. In this respect, the earliest
cartoons proposing a role for the SNAREs in exocytosis
may still be the most relevant [187]; a ‘black box’ still exists
between SNARE complex formation and the actual mem-
brane merger steps defining native fusion. Although a
mechanistic pathway to the fusion step has now been
proposed [81,82], this model requires testing in other
systems. A recent groundbreaking study clearly supports
the concept of a lipidic fusion pore, perhaps consistent with
the involvement of a proteolipid [188].
Strong evidence also exists for alternate SNARE func-
tions, in particular the regulation of Ca2 + and other ion
channels [189–197]; however, recent evidence suggests that
this represents an adapted modulatory function in mamma-
lian systems [198]. How does this, if at all, relate to the
proposed roles of SNARE complexation in fusion? One
possible explanation is that this is the actual function of the
SNAREs, to target and attach vesicles to appropriate ‘func-
tional’ sites, in part also regulating the channels and thereby
signalling pathways. It may be that accessory proteins
associated with the SNAREs (or the channel; [199,200])
mediate the actual fusion steps of exocytosis. Or, SNAREs
may simply have two (or more) separate but overlapping
roles in the exocytotic pathway. Alternatively, perhaps
SNARE complexes are artefacts of the techniques we
currently have at our disposal [201]. This is an intriguing
suggestion, implying that most SNARE complexes assayed
in vitro form as a result of sample aging and are therefore
not representative of functional native complexes. If this is
the case, it means that after tens of hours of aging in vitro,
CV SNAREs should be relegated to nonfunctional com-
plexes. Furthermore, as the same group also reports the
extremely high stability of SNARE complexes [202], CV
aged in vitro should be non-fusogenic. This is simply not the
case [36,76] [unpublished observations], again suggesting
that SNAREs do not function as the minimal fusogens of
native membranes.
Considering the CV studies, it is now reasonably certain
that the SNAREs (either alone or as complexes), having
carried out their critical upstream function(s), are not re-
quired during the Ca2 +-triggered steps of membrane fusion.
In a sense, the unfertilized urchin egg provides us with a
stage-specific ‘snapshot’ of these particular steps in the
exocytotic pathway. This would account for the speed of
the first fusion events within the population of f 15,000
fully docked and release-ready CV in an egg; fusion is at
least as fast as that measured in neuroendocrine cells, with
the lag-time after a rapid rise in [Ca2 +]free being < 10 ms
[151]. However, while eggs only undergo one such trig-
gered round of release, neurons and neuroendocrine cells are
capable of multiple high-rate rounds with appropriate stim-
uli. Cytoplasmic factors (e.g. NSF, a-SNAP and ATP)
causing disruption of cis SNARE complexes promote such
recycling by ensuring the availability of free SNAREs to
form inter-membrane complexes (e.g. priming in trans)
[145]. Thus, although we know that Ca2 +-triggered fusion
is extremely fast and seemingly optimized in neurons [150],
the implication is that the Ca2 +-triggered step(s) occurs after
SNARE action; SNAREs can promote the mechanism
without having an actual role in fusion itself. As protein
folding and conformational changes occur in the nanosec-
ond–microsecond time scale [203–205], numerous molec-
ular steps that are simply unresolved by current electro-
physiological or imaging methods could clearly occur
during the lag phase between Ca2 + entry and membrane
merger. Indeed, the time for membrane rearrangements and
merger via the stalk-pore pathway is estimated to be f 10
ns [183,206]. If Ca2 + has a role in clearing inter-membrane
SNARE complexes to promote the fusion mechanism
[36,76], this elevated [Ca2 +]free during strong stimulus
conditions would tend to promote complex disassembly.
Such a triggered loss of SNARE complexes appears to be
balanced upstream by Ca2 +-dependent SNARE complex
formation [94,207,208]. Late, fast Ca2 +-triggered disruption
of rapidly ‘zippered’ inter-membrane complexes would not
be detected in the majority of currently available assays due
to limited temporal resolution and the sheer magnitude of
concurrent reactions in (semi)intact preparations. To sum-
marize, the essential role of the SNAREs during the process
of exocytosis is undeniable, however, the evidence suggests
that they function at a pre-fusion rather than the fusion
stage.
In closing, we are reminded of Dr. G. Palade’s Nobel
Prize acceptance speech [209]:
‘‘A distinction should be made between agents directly
affecting fusion–fission and agents affecting the super-
imposed regulatory systems that activate and inactivate
the coupling between stimulation and secretion.’’
Acknowledgements
The authors wish to thank Gerald Zamponi, Roby Butt,
Joshua Kirshtein, Jeffery Lamb, Alana Luft and Sabine
Horn for discussions during the writing of this review.
J.R.C. notes many pleasant and productive conversations
with Paul Blank and Josh Zimmerberg during collaborations
on some of the work cited. J.R.C. acknowledges support of
the Alberta Heritage Foundation for Medical Research, the
Canadian Institutes of Health Research, the Heart and
Stroke Foundation of Canada and the Ruth Rannie
Memorial Fund (Faculty of Medicine, University of Cal-
gary). J.A.S. is the recipient of a Postgraduate Scholarship
Award from the Natural Sciences and Engineering Research
Council of Canada.
References
[1] R.P. Rand, V.A. Parsegian, Hydration forces between phospholipid
bilayers, Biochim. Biophys. Acta 988 (1989) 351–376.
J.A. Szule, J.R. Coorssen / Biochimica et Biophysica Acta 1641 (2003) 121–135130
[2] R.P. Rand, The lipid–water interface: revelations by osmotic stress,
Int. Rev. Cyt. 215 (2002) 33–48.
[3] P.I. Kuzmin, J. Zimmerberg, Y.A. Chizmadzhev, F.S. Cohen, A
quantitative model for membrane fusion based on low-energy inter-
mediates, Proc. Natl. Acad. Sci. U. S. A. 98 (2001) 7235–7240.
[4] V.S. Markin, J.P. Albanes, Membrane fusion: stalk model revisited,
Biophys. J. 82 (2002) 693–712.
[5] Y. Kozlovsky, M.M. Kozlov, Stalk model of membrane fusion: sol-
ution of energy crisis, Biophys. J. 82 (2002) 882–895.
[6] R.A. Chavez, S.G. Miller, H.P. Moore, A biosynthetic secretory
pathway in constitutive secretory cells, J. Cell Biol. 133 (1996)
1177–1191.
[7] J.R. Coorssen, H. Schmidt, W. Almers, Ca2 + triggers massive
exocytosis in Chinese hamster ovary cells, EMBO J. 15 (1996)
3787–3791.
[8] Y. Ninomiya, T. Kishimoto, Y. Miyashita, H. Kasai, Ca2 +-depend-
ent exocytotic pathways in Chinese hamster ovary fibroblasts re-
vealed by a caged-Ca2 + compound, J. Biol. Chem. 271 (1996)
17751–17754.
[9] Y. Dan, M.M. Poo, Quantal transmitter secretion from myocytes
loaded with acetylcholine, Nature 359 (1992) 733–736.
[10] E. Bugnard, N. Taulier, A. Bloc, P. Correges, J. Falk-Vairant, P. Sors,
F. Loctin, Y. Dunant, Quantal transmitter release by glioma cells:
quantification of intramembrane particle changes, Neuroscience 113
(2002) 125–135.
[11] D.E. Knight, H. von Grafenstein, C.M. Athayde, Calcium-dependent
and calcium-independent exocytosis, Trends Neurosci. 12 (1989)
451–458.
[12] V.D. Vacquier, The isolation of intact cortical granules from sea
urchin eggs: calcium ions trigger granule discharge, Dev. Biol. 43
(1975) 62–74.
[13] P.F. Baker, M.J. Whitaker, Influence of ATP and calcium on the
cortical reaction in sea urchin eggs, Nature 276 (1978) 513–515.
[14] J. Vilmart-Seuwen, H. Kersken, R. Sturzl, H. Plattner, ATP keeps
exocytosis sites in a primed state but is not required for membrane
fusion: an analysis with Paramecium cells in vivo and in vitro, J.
Cell Biol. 103 (1986) 1279–1288.
[15] R.W. Holz, M.A. Bittner, S.C. Peppers, R.A. Senter, D.A. Eberhard,
MgATP-independent and MgATP-dependent exocytosis, J. Biol.
Chem. 264 (1989) 5412–5419.
[16] J.C. Hay, T.F. Martin, Resolution of regulated secretion into sequen-
tial MgATP-dependent and calcium-dependent stages mediated by
distinct cytosolic proteins, J. Cell Biol. 119 (1992) 139–151.
[17] J.C. Hay, P.L. Fisette, G.H. Jenkins, K. Fukami, T. Takenawa,
R.A. Anderson, T.F.J. Martin, ATP-dependent inositide phosphor-
ylation required for Ca2 +-activated secretion, Nature 374 (1995)
173–177.
[18] T. Parsons, J.R. Coorssen, H. Horstmann, W. Almers, Docked gran-
ules, the exocytotic burst, and the need for ATP hydrolysis in endo-
crine cells, Neuron 15 (1995) 1085–1096.
[19] H. Plattner, A.R. Artalejo, E. Neher, Ultrastructural organization of
bovine chromaffin cell cortex—analysis by cryofixation and morph-
ometry of aspects pertinent to exocytosis, J. Cell Biol. 139 (1997)
1709–1717.
[20] S. Barg, L. Eliasson, E. Renstrom, P. Rorsman, A subset of 50
secretory granules in close contact with L-type Ca2 + channels ac-
counts for first-phase insulin secretion in mouse h-cells, Diabetes 51(2002) S74–S82.
[21] R. Heidelberger, P. Sterling, G. Matthews, Roles of ATP in depletion
and replenishment of the releasable pool of synaptic vesicles, J.
Neurophysiol. 88 (2002) 98–106.
[22] T.H. Sollner, M.K. Bennett, S.W. Whitheart, R.H. Scheller, J.E.
Rothman, A protein assembly–disassembly pathway in vitro that
may correspond to sequential steps of synaptic vesicle docking,
activation, and fusion, Cell 75 (1993) 409–418.
[23] J.E. Rothman, Mechanisms of intracellular protein transport, Nature
372 (1994) 55–63.
[24] S.H. Gerber, T.C. Sudhof, Molecular determinants of regulated exo-
cytosis, Diabetes 51 (2002) S3–S11.
[25] B. Storrie, M. Desjardins, The biogenesis of lysosomes: is it a kiss
and run, continuous fusion and fission process? BioEssays 18 (1996)
895–903.
[26] E. Ales, L. Tabares, J.M. Poyato, V. Valero, M. Lindau, G.
Alvarez de Toledo, High calcium concentrations shift the mode
of exocytosis to the kiss-and-run mechanism, Nat. Cell Biol. 1
(1999) 40–44.
[27] A.W. Henkel, G. Kang, J. Kornhuber, A common molecular machi-
nery for exocytosis and the ‘kiss-and-run’ mechanism in chromaffin
cells is controlled by phosphorylation, J. Cell Sci. 114 (2001)
4613–4620.
[28] J. Hartmann, M. Lindau, A novel Ca2 +-dependent step in exocytosis
subsequent to vesicle fusion, FEBS Lett. 363 (1995) 217–220.
[29] R. Fernandez-Chacon, G. Alvarez de Toledo, Cytosolic calcium
facilitates release of secretory products after exocytotic vesicle fu-
sion, FEBS Lett. 363 (1995) 221–225.
[30] S. Scepek, J.R. Coorssen, M. Lindau, Fusion pore expansion in
horse eosinophils is modulated by Ca2 + and protein kinase C via
distinct mechanisms, EMBO J. 17 (1998) 4340–4345.
[31] R. Rahamimoff, J.M. Fernandez, Pre- and postfusion regulation of
transmitter release, Neuron 18 (1997) 17–27.
[32] V.N. Murthy, T.J. Sejnowski, C.F. Stevens, Heterogeneous release
properties of visualized individual hippocampal synapses, Neuron
18 (1997) 599–612.
[33] V.N. Murthy, C.F. Stevens, Reversal of synaptic vesicle docking at
central synapses, Nat. Neurosci. 2 (1999) 503–507.
[34] J. Shorter, M.B. Beard, J. Seemann, A.B. Dirac-Svejstrup, G. War-
ren, Sequential tethering of golgins and catalysis of SNAREpin
assembly by the vesicle-tethering protein p115, J. Cell Biol. 157
(2002) 45–62.
[35] J.R.C. Whyte, S. Munro, Vesicle tethering complexes in membrane
traffic, J. Cell Sci. 115 (2002) 2627–2637.
[36] J. Zimmerberg, P. Blank, I. Kolosova, M.S. Cho, M. Tahara, J.R.
Coorssen, A stage-specific preparation to study the Ca2 +-triggered
fusion steps of exocytosis: rationale and perspectives, Biochimie 82
(2000) 303–314.
[37] D. Bruns, R. Jahn, Molecular determinants of exocytosis, Pflugers
Arch. 443 (2002) 333–338.
[38] S.L. Leikin, M.M. Kozlov, L.V. Chernomordik, V.S. Markin,
Y.A. Chizmadzhev, Membrane fusion: overcoming of the hydra-
tion barrier and local restructuring, J. Theor. Biol. 129 (1987)
411–425.
[39] L. Chernomordik, Non-bilayer lipids and biological fusion inter-
mediates, Chem. Phys. Lipids 81 (1996) 203–213.
[40] Y. Kozlovsky, L.V. Chernomordik, M.M. Kozlov, Lipid intermedi-
ates in membrane fusion: formation, structure, and decay of hemi-
fusion diaphragm, Biophys. J. 83 (2002) 2634–2651.
[41] G. Schiavo, M. Matteoli, C. Montecucco, Neurotoxins affecting
neuroexocytosis, Physiol. Rev. 80 (2000) 717–766.
[42] G. Schiavo, F. Benfenati, B. Poulain, O. Rossetto, P. Polverino de
Laureto, B.R. DasGupta, C. Montecucco, Tetanus and botulinum-B
neurotoxins block neurotransmitter release by proteolytic cleavage
of synaptobrevin, Nature 359 (1992) 832–835.
[43] G. Schiavo, C.C. Shone, O. Rossetto, F.C.G. Alexander, C. Monte-
cucco, Botulinum neurotoxin serotype F is a zinc endopeptidase
specific for VAMP/synaptobrevin, J. Biol. Chem. 268 (1993)
11516–11519.
[44] Y. Humeau, F. Doussau, N.J. Grant, B. Poulain, How botulinum and
tetanus neurotoxins block neurotransmitter release, Biochimie 82
(2000) 427–446.
[45] A.M. Harvey, The peripheral action of tetanus toxin, J. Physiol. 96
(1939) 348–365.
[46] A.S.V. Burgen, F. Dickens, L.J. Zatman, The action of botulinum
toxin on the neuro-muscular junction, J. Physiol. 109 (1949) 10–24.
[47] D.A. Boroff, J. DelCastillo, W.H. Evoy, R.A. Steinhardt, Observa-
J.A. Szule, J.R. Coorssen / Biochimica et Biophysica Acta 1641 (2003) 121–135 131
tions on the actions of type A botulinum toxin on frog neuromus-
cular junctions, J. Physiol. 240 (1974) 227–253.
[48] S.Y. Hua, M.P. Charlton, Activity-dependent changes in partial
VAMP complexes during neurotransmitter release, Nat. Neurosci.
2 (1999) 1078–1083.
[49] V.B. Brooks, The action of botulinum toxin on motor-nerve fila-
ments, J. Physiol. 123 (1954) 501–515.
[50] V.B. Brooks, An intracellular study of the action of repetitive nerve
volleys and of botulinum toxin on miniature end-plate potentials, J.
Physiol. 134 (1956) 264–277.
[51] S. Thesleff, Supersensitivity of skeletal muscle produced by botuli-
num toxin, J. Physiol. 151 (1960) 598–607.
[52] F. Dreyer, A. Schmitt, Transmitter release in tetanus and botulinum
A toxin-poisoned mammalian motor endplates and its dependence
on nerve stimulation and temperature, Pflugers Arch. 399 (1983)
228–234.
[53] R.L. Parsons, W.W. Hofmann, G.A. Feigen, Mode of action of tet-
anus toxin on the neuromuscular junction, Am. J. Physiol. 210
(1966) 84–90.
[54] A.J. Harris, R. Miledi, The effect of type D botulinum toxin on frog
neuromuscular junctions, J. Physiol. 217 (1971) 497–515.
[55] L.W. Duchen, D.A. Tonge, The effects of tetanus toxin on neuro-
muscular transmission and on the morphology of motor end-plates in
slow and fast skeletal muscle of the mouse, J. Physiol. 228 (1973)
157–172.
[56] B.A. Stewart, M. Mohtashami, W.S. Trimble, G.L. Boulianne,
SNARE proteins contribute to calcium cooperativity of synaptic
transmission, Proc. Natl. Acad. Sci. U. S. A. 97 (2000) 13955–13960.
[57] M.F. Finley, S.M. Patel, D.V. Madison, R.H. Scheller, The core
membrane fusion complex governs the probability of synaptic
vesicle fusion but not transmitter release kinetics, J. Neurosci. 22
(2002) 1266–1272.
[58] J. Mellanby, P.A. Thompson, The effect of tetanus toxin at the
neuromuscular junction in the goldfish, J. Physiol. 224 (1972)
407–419.
[59] S.G. Cull-Candy, H. Lundh, S. Thesleff, Effects of botulinum toxin
on neuromuscular transmission in the rat, J. Physiol. 260 (1976)
177–203.
[60] M. Gansel, R. Penner, F. Dreyer, Distinct sites of action of clostridial
neurotoxins revealed by double-poisoning of mouse motor nerve
terminals, Pflugers Arch. 409 (1987) 533–539.
[61] F. Dreyer, F. Rosenberg, C. Becker, H. Bigalke, R. Penner, Differential
effects of various secretagogues on quantal transmitter release from
mouse motor nerve terminals treated with botulinum A and tetanus
toxin, Naunyn-Schmiedeberg’s Arch. Pharmacol. 335 (1987) 1–7.
[62] A.C. Ashton, J.O. Dolly, Microtubule-dissociating drugs and
A23187 reveal differences in the inhibition of synaptosomal trans-
mitter release by botulinum neurotoxins types A and B, J. Neuro-
chem. 56 (1991) 827–835.
[63] G.W. Lawrence, U. Weller, J.O. Dolly, Botulinum A and the light
chain of tetanus toxin inhibit distinct stages of MgATP-dependent
catecholamine exocytosis from permeabilised chromaffin cells, Eur.
J. Biochem. 222 (1994) 325–333.
[64] G.W. Lawrence, P. Foran, J.O. Dolly, Distinct exocytotic re-
sponses of intact and permeabilized chromaffin cells after cleav-
age of the 25-kDa synaptosomal-associated protein (SNAP-25) or
synaptobrevin by botulinum toxin A or B, Eur. J. Biochem. 236
(1996) 877–886.
[65] M.A. Bittner, R.W. Holz, Protein kinase C and clostridial neurotox-
ins affect discrete and related steps in the secretory pathway, Cell.
Mol. Neurobiol. 13 (1993) 649–664.
[66] G. Ahnert-Hilger, U. Weller, Comparison of the intracellular effects
of clostridial neurotoxins on exocytosis from streptolysin O-permea-
bilized rat pheochromocytoma (PC12) and bovine adrenal chromaf-
fin cells, Neuroscience 53 (1993) 547–552.
[67] D.E. Glenn, R.D. Burgoyne, Botulinum neurotoxin light chains in-
hibit both Ca2 +-induced and GTP analogue-induced catecholamine
release from permeabilised adrenal chromaffin cells, FEBS Lett. 386
(1996) 137–140.
[68] M. Capogna, R.A. McKinney, V. O’Connor, B.H. Gahwiler, S.M.
Thompson, Ca2 + or Sr2 + partially rescues synaptic transmission in
hippocampal cultures treated with botulinum toxin A and C, but not
tetanus toxin, J. Neurosci. 17 (1997) 7190–7202.
[69] J. Land, H. Zhang, V.V. Vaidyanathan, K. Sadoul, H. Niemann, C.B.
Wollheim, Transient expression of botulinum neurotoxin C1 light
chain differentially inhibits calcium and glucose induced insulin
secretion in clonal beta-cells, FEBS Lett. 419 (1997) 13–17.
[70] T. Xu, T. Binz, H. Niemann, E. Neher, Multiple kinetic components
of exocytosis distinguished by neurotoxin sensitivity, Nat. Neurosci.
1 (1998) 192–200.
[71] S.Y. Hua, D.A. Raciborska, W.S. Trimble, M.P. Charlton, Different
VAMP/synaptobrevin complexes for spontaneous and evoked trans-
mitter release at the crayfish neuromuscular junction, J. Neurophy-
siol. 80 (1998) 3233–3246.
[72] R. Regazzi, C.B. Wollheim, J. Lang, J.M. Theler, O. Rossetto, C.
Montecucco, K. Sadoul, U. Weller, M. Palmer, B. Thorens, VAMP-2
and cellubrevin are expressed in pancreatic b-cells and are essential
for Ca2 +- but not for GTPgS-induced insulin secretion, EMBO J. 15
(1995) 2723–2730.
[73] A. Fassio, R. Sala, G. Bonanno, M. Marchi, M. Raiteri, Evidence for
calcium-dependent vesicular transmitter release insensitive to tetanus
and botulinum toxin type F, Neuroscience 90 (1999) 893–902.
[74] S.S. Vogel, J. Zimmerberg, Proteins on exocytotic vesicles mediate
calcium-triggered fusion, Proc. Natl. Acad. Sci. U. S. A. 89 (1992)
4749–4753.
[75] J.R. Coorssen, P.S. Blank, M. Tahara, J. Zimmerberg, Biochem-
ical and functional studies of cortical vesicle fusion: the
SNARE complex and Ca2 + sensitivity, J. Cell Biol. 143
(1998) 1845–1857.
[76] M. Tahara, J.R. Coorssen, K. Timmers, P.S. Blank, T. Whalley, R.H.
Scheller, J. Zimmerberg, Calcium can disrupt the SNARE protein
complex on sea urchin egg secretory vesicles without irreversibly
blocking fusion, J. Biol. Chem. 273 (1998) 33667–33673.
[77] J.R. Coorssen, M. Tahara, P. Blank, J. Zimmerberg, Role of SNARE
proteins in membrane fusion, Mol. Biol. Cell 8 (1997) 296a.
[78] G.Q. Bi, J.M. Alderton, R.A. Steinhardt, Calcium-regulated exocy-
tosis is required for cell membrane resealing, J. Cell Biol. 131 (1995)
1747–1758.
[79] C. Ungermann, B.J. Nichols, H.R.B. Pelham, W. Wickner, A vacuo-
lar v– t-SNARE complex, the predominant form in vivo and on
isolated vacuoles, is disassembled and activated for docking and
fusion, J. Cell Biol. 140 (1998) 61–69.
[80] C. Ungermann, K. Sato, W. Wickner, Defining the functions of
trans-SNARE pairs, Nature 396 (1998) 543–548.
[81] C. Peters, M.J. Bayer, S. Buhler, J.S. Andersen, M. Mann, A. Mayer,
Trans-complex formation by proteolipid channels in the terminal
phase of membrane fusion, Nature 409 (2001) 567–568.
[82] O. Muller, M.J. Bayer, C. Peters, J.S. Andersen, M. Mann, A.
Mayer, The Vtc proteins in vacuolar fusion: coupling NSF ac-
tivity to V(0) trans-complex formation, EMBO J. 21 (2002)
259–269.
[83] J.E. Smolen, S.J. Stoehr, L.A. Boxer, Human neutrophils permeabi-
lized with digitonin respond with lysosomal enzyme release when
exposed to micromolar levels of free calcium, Biochim. Biophys.
Acta 886 (1986) 1–17.
[84] A. Rodriguez, P. Webster, J. Ortego, N.W. Andrews, Lysosomes
behave as Ca2 +-regulated exocytotic vesicles in fibroblasts and epi-
thelial cells, J. Cell Biol. 137 (1997) 93–104.
[85] F.T. Horrigan, R.J. Bookman, Releasable pools and the kinetics
of exocytosis in adrenal chromaffin cells, Neuron 13 (1994)
1119–1129.
[86] S. Kirischuk, R. Grantyn, A readily releasable pool of single inhib-
itory boutons in culture, NeuroReport 11 (2000) 3709–3713.
[87] T. Moser, E. Neher, Rapid exocytosis in single chromaffin cells
J.A. Szule, J.R. Coorssen / Biochimica et Biophysica Acta 1641 (2003) 121–135132
recorded from mouse adrenal slices, J. Neurosci. 17 (1997)
2314–2323.
[88] J.Y. Sun, L.G. Wu, Fast kinetics of exocytosis revealed by simulta-
neous measurements of presynaptic capacitance and postsynaptic
currents at a central synapse, Neuron 30 (2001) 171–182.
[89] Y. Yang, S. Udayasankar, J. Dunning, P. Chen, K.D. Gillis, A
highly Ca2 +-sensitive pool of vesicles is regulated by protein kin-
ase C in adrenal chromaffin cells, Proc. Natl. Acad. Sci. U. S. A.
99 (2002) 17060–17065.
[90] J.A. Steyer, H. Horstmann, W. Almers, Transport, docking and exo-
cytosis of single secretory granules in live chromaffin cells, Nature
388 (1997) 474–478.
[91] J.R. Coorssen, P.S. Blank, F. Albertorio, L. Bezrukov, I. Kolosova,
P.S. Backlund, J. Zimmerberg, Quantitative femto- to attomole im-
munodetection of regulated secretory vesicle proteins critical to exo-
cytosis, Anal. Biochem. 307 (2002) 54–62.
[92] T. Xu, B. Rammner, M. Margittai, A.R. Artalejo, E. Neher, R. Jahn,
Inhibition of SNARE complex assembly differentially affects kinetic
components of exocytosis, Cell 99 (1999) 713–722.
[93] Y.A. Chen, S.J. Scales, J.R. Jagath, R.H. Scheller, A discontinuous
SNAP-25 C-terminal coil supports exocytosis, J. Biol. Chem. 276
(2001) 28503–28508.
[94] Y.A. Chen, S.J. Scales, S.M. Patel, Y.C. Doung, R.H. Scheller,
SNARE complex formation is triggered by Ca2 + and drives mem-
brane fusion, Cell 97 (1999) 165–174.
[95] P. Ray, J.D. Berman, W. Middleton, J. Brendle, Botulinum toxin
inhibits arachadonic acid release associated with acetylcholine re-
lease from PC12 cells, J. Biol. Chem. 268 (1993) 11057–11064.
[96] P. Ray, C.B. Millaed, J.P. Petrali, J.D. Berman, R. Ray, Acetylcho-
line exocytosis in PC12 cells deficient in SNAP-25, NeuroReport 8
(1997) 2271–2274.
[97] P. Presek, S. Jessen, F. Dreyer, P.E. Jarvie, D. Findik, P.R. Dunk-
ley, Tetanus toxin inhibits depolarization-stimulated protein phos-
phorylation in rat cortical synaptosomes: effect on synapsin I
phosphorylation and translocation, J. Neurochem. 59 (1992)
1336–1343.
[98] R.V. Considine, C.M. Handler, L.L. Simpson, J.R. Sherwin, Tetanus
toxin inhibits neurotensin-induced mobilization of cytosolic protein
kinase C activity in NG-108 cells, Toxicon 29 (1991) 1351–1357.
[99] A. Najib, P. Pelliccioni, C. Gil, J. Aguilera, Clostridium neurotoxins
influence serotonin uptake and release differently in rat brain syn-
aptosomes, J. Neurochem. 72 (1999) 1991–1998.
[100] H. Caohuy, H.B. Pollard, Annexin 7: a non-SNARE proteolytic
substrate for botulinum toxin type C in secreting chromaffin cells,
Ann. N.Y. Acad. Sci. 971 (2002) 287–290.
[101] K.L. Schulze, K. Broadie, M.S. Perin, H.J. Bellen, Genetic and
electrophysiological studies of Drosophila syntaxin-1A demonstrate
its role in non-neuronal secretion and neurotransmission, Cell 80
(1995) 311–320.
[102] M.L. Nonet, K. Grundahl, B.J. Meyer, J.B. Rand, Synaptic function
is impaired but not eliminated in C. elegans mutants lacking synap-
totagmin, Cell 73 (1993) 1291–1305.
[103] M.L. Nonet, O. Saifee, H. Zhao, J.B. Rand, L. Wei, Synaptic trans-
mission deficits in Caenorhabditis elegans synaptobrevin mutants, J.
Neurosci. 18 (1998) 70–80.
[104] D.L. Deitcher, A. Ueda, B.A. Stewart, R.W. Burgess, Y. Kidokoro,
T.L. Schwarz, Distinct requirements for evoked and spontaneous
release of neurotransmitter are revealed by mutations in the Dro-
sophila gene neuronal-synaptobrevin, J. Neurosci. 18 (1998)
2028–2039.
[105] S.S. Rao, B.A. Stewart, P.K. Rivlin, I. Vilinsky, B.O. Watson, C.
Lang, G. Boulianne, M.M. Salpeter, D.L. Deitcher, Two distinct
effects on neurotransmission in a temperature-sensitive SNAP-25
mutant, EMBO J. 20 (2001) 6761–6771.
[106] M.A. Bittner, M.K. Bennett, R.W. Holz, Evidence that syntaxin 1A
is involved in storage in the secretory pathway, J. Biol. Chem. 271
(1996) 11214–11221.
[107] S. Nagamatsu, T. Fujiwara, Y. Nakamichi, T. Watanabe, H. Katahira,
H. Sawa, K. Akagawa, Expression and functional role of syntaxin 1/
HPC-1 in pancreatic beta cells. Syntaxin 1A, but not 1 B, plays a
negative role in regulatory insulin release pathway, J. Biol. Chem.
271 (1996) 1160–1165.
[108] S. Nagamatsu, Y. Nakamichi, C. Yamamura, S. Matsushima, T. Wa-
tanabe, S. Ozawa, H. Furukawa, H. Ishida, Decreased expression of
t-SNARE, syntaxin 1, and SNAP-25 in pancreatic beta cells is in-
volved in impaired insulin secretion from diabetic GK rat islets:
restoration of decreased t-SNARE proteins improves impaired insu-
lin secretion, Diabetes 48 (1999) 2367–2373.
[109] R. Regazzi, K. Sadoul, P. Meda, R.B. Kelly, P.A. Halban, C.B.
Wollheim, Mutational analysis of VAMP domains implicated in
Ca2 +-induced insulin exocytosis, EMBO J. 15 (1996) 6951–6959.
[110] P. Washbourne, N. Bortoletto, M.E. Graham, M.C. Wilson, R.D.
Burgoyne, C. Montecucco, Botulinum neurotoxin E-insensitive mu-
tants of SNAP-25 fail to bind VAMP but support exocytosis, J.
Neurochem. 73 (1999) 2424–2433.
[111] M.E. Graham, P. Washbourne, M.C. Wilson, R.D. Burgoyne, SNAP-
25 with mutations in the zero layer supports normal membrane fu-
sion kinetics, J. Cell Sci. 114 (2001) 4397–4405.
[112] P. Washbourne, P.M. Thompson, M. Carta, E.T. Costa, J.R. Mathews,
G. Lopez-Bendito, Z. Molnar, M.W. Becher, C.F. Valenzuela, L.D.
Partridge, M.C. Wilson, Genetic ablation of the t-SNARE SNAP-25
distinguishes mechanisms of neuroexocytosis, Nat. Neurosci. 5
(2001) 19–26.
[113] S. Schoch, F. Deak, A. Konigstorfer, M. Mozhayeva, Y. Sara, T.C.
Sudhof, E.T. Kavalali, SNARE function analyzed in synaptobrevin/
VAMP knockout mice, Science 294 (2001) 1117–1122.
[114] S.J. Scales, M.F.A. Finley, R.H. Scheller, Fusion without SNAREs?
Science 294 (2001) 1015–1016.
[115] I. Vilinsky, B.A. Stewart, J. Drummond, I. Robinson, D.L. Deitcher,
A drosophila SNAP-25 null mutant reveals context-dependent redun-
dancy with SNAP-24 in neurotransmission, Genetics 162 (2002)
259–271.
[116] T.T. Liu, C. Barlow, Analysis of Sec22p in endoplasmic reticulum/
golgi transport reveals cellular redundancy in SNARE protein func-
tion, Mol. Biol. Cell 13 (2002) 3314–3324.
[117] K. Sadoul, A. Berger, H. Niemann, U. Weller, P.A. Roche, A. Klip,
W.S. Trimble, R. Regazzi, S. Catsicas, P.A. Halban, SNAP-23 is
not cleaved by botulinum neurotoxin E and can replace SNAP-25
in the process of insulin secretion, J. Biol. Chem. 272 (1997)
33023–33027.
[118] J. Zimmerberg, J.R. Coorssen, S.S. Vogel, P.S. Blank, Topical re-
view: sea urchin egg preparations as systems for the study of cal-
cium-triggered exocytosis, J. Physiol. 520 (1999) 15–21.
[119] K. Hu, J. Carroll, C. Rickman, B. Davletov, Action of complexin on
SNARE complex, J. Biol. Chem. 277 (2002) 41652–41656.
[120] S.J. Scales, B.A. Hesser, E.S. Masuda, R.H. Scheller, Amisyn, a
novel syntaxin-binding protein that may regulate SNARE complex
assembly, J. Biol. Chem. 277 (2002) 28271–28279.
[121] S. Conner, D. Leaf, G. Wessel, Members of the SNARE hypothesis
are associated with cortical granule exocytosis in the sea urchin egg,
Mol. Reprod. Dev. 48 (1997) 106–118.
[122] J.R. Coorssen, P.S. Blank, I. Kolosova, P. Backlund, J. Zimmerberg,
Are SNARE proteins necessary and sufficient for membrane fusion?
Mol. Biol. Cell 10 (1999) 219a.
[123] J.R. Coorssen, P.S. Blank, F. Albertorio, L. Bezrukov, I. Kolosova,
X. Chen, P. Backlund, J. Zimmerberg, Regulated secretion: SNARE
density, vesicle fusion, and calcium dependence, J. Cell Sci. 116
(2003) 2087–2097 (in press).
[124] S. Leikin, V.A. Parsegian, D.C. Rau, R.P. Rand, Hydration forces,
Annu. Rev. Phys. Chem. 44 (1993) 369–395.
[125] D.P. Siegel, Energetics of intermediates in membrane fusion: com-
parison of stalk and inverted micellar intermediate mechanisms, Bi-
ophys. J. 65 (1993) 2124–2140.
[126] D. David, S. Sundarababu, J.E. Gerst, Involvement of long chain
J.A. Szule, J.R. Coorssen / Biochimica et Biophysica Acta 1641 (2003) 121–135 133
fatty acid elongation in the trafficking of secretory vesicles in yeast,
J. Cell Biol. 143 (1998) 1167–1182.
[127] E. Grote, M. Baba, Y. Ohsumi, P.J. Novick, Geranylgeranylated
SNAREs are dominant inhibitors of membrane fusion, J. Cell Biol.
151 (2000) 453–465.
[128] D. Langosh, J.M. Crane, B. Brosig, A. Hellwig, L.K. Tamm, J.
Reed, Peptide mimics of SNARE transmembrane segments drive
membrane fusion depending on their conformational plasticity, J.
Mol. Biol. 311 (2001) 709–721.
[129] S.S. Vogel, L.V. Chernomordik, J. Zimmerberg, Calcium-triggered
fusion of exocytotic granules requires proteins in only one mem-
brane, J. Biol. Chem. 267 (1992) 25640–25643.
[130] A. Chanturiya, M. Whitaker, J. Zimmerberg, Calcium-induced fu-
sion of sea urchin egg secretory vesicles with planar phospholipid
bilayer membranes, Mol. Membr. Biol. 16 (1999) 89–94.
[131] S. Kagiwada, M. Murata, R. Hishida, M. Tagaya, S. Yamashina, S.
Ohnishi, In vitro fusion of rabbit liver golgi membranes with lip-
osomes, J. Biol. Chem. 268 (1993) 1430–1435.
[132] M. Vidal, D. Hoekstra, In vitro fusion of reticulocyte endocytic
vesicles with liposomes, J. Biol. Chem. 270 (1995) 17823–17829.
[133] J.M. Smit, G. Li, P. Schoen, J. Corver, R. Bittman, K.C. Lin, J.
Wilschut, Fusion of alphavirus with liposomes is a non-leaky proc-
ess, FEBS Lett. 521 (2002) 62–66.
[134] H. Mizuguchi, T. Nakanishi, M. Kondoh, T. Nakagawa, M. Naka-
nishi, T. Matsuyama, Y. Tsutsumi, S. Nakagawa, T. Mayumi, Fusion
of sendai virus with liposome depends on only F protein, but not HN
protein, Virus Res. 59 (1999) 191–201.
[135] E.I. Hernandez-Jimenez, V.I. Razinkov, I.I. Mikhalyov, A.V. Koz-
minykh, F.S. Cohen, J.G. Molotkovsky, Selective labeling of the
inner liposome leaflet by fluorescent lipid probes, and studies of
liposome fusion with influenza virus, Membr. Cell Biol. 11 (1997)
515–527.
[136] M.M. Kozlov, L.V. Chernomordik, A mechanism of protein-medi-
ated fusion: coupling between refolding of the influenza hemagglu-
tinin and lipid rearrangements, Biophys. J. 75 (1998) 1384–1396.
[137] T. Weber, B.V. Zemelman, J.A. McNew, B. Westermann, M.
Gmachl, F. Parlati, T.H. Sollner, J.E. Rothman, SNAREpins: mini-
mal machinery for membrane fusion, Cell 92 (1998) 759–772.
[138] S. Pabst, M. Margittai, D. Vainius, R. Langen, R. Jahn, D. Fasshauer,
Rapid and selective binding to the synaptic SNARE complex sug-
gests a modulatory role of complexins in neuroexicytosis, J. Biol.
Chem. 277 (2002) 7838–7848.
[139] C. Lang, D. Bruns, D. Wenzel, D. Riedel, P. Holroyd, C. Thiele, R.
Jahn, SNAREs are concentrated in cholesterol-dependent clusters
that define docking and fusion sites for exocytosis, EMBO J. 20
(2001) 2202–2213.
[140] F. Parlati, T. Weber, J.A. McNew, B. Westermann, T.H. Sollner,
J.E. Rothman, Rapid and efficient fusion of phospholipid vesicles
by the a-core of a SNARE complex in the absence of an N-
terminal regulatory domain, Proc. Natl. Acad. Sci. U. S. A. 96
(1999) 12565–12570.
[141] W. Nickel, T. Weber, J.A. McNew, F. Parlati, T.H. Sollner, J.E.
Rothman, Content mixing and membrane integrity during membrane
fusion driven by pairing of isolated v-SNAREs and t-SNAREs,
Proc. Natl. Acad. Sci. U. S. A. 96 (1999) 12571–12576.
[142] L.K. Mahal, S.M. Sequeira, J.M. Gureasko, T.H. Sollner, Calcium-
independent stimulation of membrane fusion and SNAREpin forma-
tion by synaptotagmin I, J. Cell Biol. 158 (2002) 273–282.
[143] T.J. Melia, T. Weber, J.A. McNew, L.E. Fisher, R.J. Johnston, F.
Parlati, L.K. Mahal, T.H. Sollner, J.E. Rothman, Regulation of mem-
brane fusion by the membrane-proximal coil of the t-SNARE during
zippering of SNAREpins, J. Cell Biol. 158 (2002) 929–940.
[144] R. Fukuda, J.A. McNew, T. Weber, F. Parlati, T. Engel, W. Nickel,
J.E. Rothman, T.H. Sollner, Functional architecture of an intracellu-
lar membrane t-SNARE, Nature 407 (2000) 198–202.
[145] T. Weber, F. Parlati, J.A. McNew, R.J. Johnston, B. Westermann,
T.H. Sollner, J.E. Rothman, SNAREpins are functionally resistant
to disruption by NSF and aSNAP, J. Cell Biol. 149 (2000)
1063–1072.
[146] J.A. McNew, T. Weber, F. Parlati, R.J. Johnston, T.J. Melia, T.H.
Sollner, J.E. Rothman, Close is not enough: SNARE-dependent
membrane fusion requires an active mechanism that transduces force
to membrane anchors, J. Cell Biol. 150 (2000) 105–117.
[147] R.B. Sutton, D. Fasshauer, R. Jahn, A.T. Brunger, Crystal structure
of a SNARE complex involved in synaptic exocytosis at 2.4 A
resolution, Nature 395 (1998) 347–353.
[148] F. Pincet, L. Lebeau, S. Cribier, Short-range specific forces are able
to induce hemifusion, Eur. Biophys. J. 30 (2001) 91–97.
[149] Y. Cajal, J.M. Boggs, M.K. Jain, Salt-triggered intermembrane ex-
change of phospholipids and hemifusion by myelin basic protein,
Biochemistry 36 (1997) 2566–2576.
[150] B.L. Sabatini, W.G. Regehr, Timing of neurotransmission at fast
synapses in the mammalian brain, Nature 384 (1996) 170–172.
[151] N.I. Shafi, S.S. Vogel, J. Zimmerberg, Using caged calcium to study
sea urchin egg corticle granule exocytosis in vitro, Methods 6 (1994)
82–92.
[152] K. Hu, J. Carroll, S. Fedorovich, C. Rickman, A. Sukhodub, B.
Davletov, Vesicular restriction of synaptobrevin suggests a role for
calcium in membrane fusion, Nature 415 (2002) 646–650.
[153] C.E. Creutz, Cis-unsaturated fatty acids induce the fusion of chro-
maffin granules aggregated by synexin, J. Cell Biol. 91 (1981)
247–256.
[154] S. Schenkman, P.S. De Araujo, A. Sesso, F.H. Quina, H. Chaimo-
vich, A kinetic and structural study of two-step aggregation and
fusion of neutral phospholipid vesicles promoted by serum albumin
at low pH, Chem. Phys. Lipids 28 (1981) 165–180.
[155] R. Blumenthal, M. Henkart, C.J. Steer, Clathrin-induced pH-depend-
ent fusion of phosphatidylcholine vesicles, J. Biol. Chem. 258
(1983) 3409–3415.
[156] R. Sundler, J. Wijkander, Protein-mediated intermembrane contact
specifically enhances Ca2 +-induced fusion of phosphatidate-contain-
ing membranes, Biochim. Biophys. Acta 730 (1983) 391–394.
[157] T.M. Young, J.D. Young, Protein-mediated intermembrane contact
facilitates fusion of lipid vesicles with planar bilayers, Biochim.
Biophys. Acta 775 (1984) 441–445.
[158] G. Fujii, M.E. Selsted, D. Eisenberg, Defensins promote fusion and
lysis of negatively charged membranes, Protein Sci. 2 (1993)
1301–1312.
[159] P.E. Glaser, R.W. Gross, Rapid plasmenylethanolamine-selective fu-
sion of membrane bilayers catalyzed by an isoform of glyceralde-
hyde-3-phosphate dehydrogenase: discrimination between glycolytic
and fusogenic roles of individual isoforms, Biochemistry 34 (1995)
12193–12203.
[160] R.J. Hessler, R.A. Blackwood, T.G. Brock, J.W. Francis, D.M.
Harsh, J.E. Smolen, Identification of glyceraldehyde-3-phosphate
dehydrogenase as a Ca2 +-dependent fusogen in human neutrophil
cytosol, J. Leukoc. Biol. 63 (1998) 331–336.
[161] M. Otter-Nilsson, R. Hendriks, E.I. Pecheur-Huet, D. Hoekstra, T.
Nilsson, Cytosolic ATPases, p97 and NSF, are sufficient to mediate
rapid membrane fusion, EMBO J. 18 (1999) 2074–2083.
[162] B. Brugger, W. Nickel, T. Weber, F. Parlati, J.A. McNew, J.E. Roth-
man, T.H. Sollner, Putative fusogenic activity of NSF is restricted to
a lipid mixture whose coalescence is also triggered by other factors,
EMBO J. 19 (2000) 1272–1278.
[163] A. Agirre, S. Nir, J.L. Nieva, J. Dijkstra, Induction of aggregation
and fusion of cholesterol-containing membrane vesicles by an anti-
cholesterol monoclonal antibody, J. Lipid Res. 41 (2000) 621–628.
[164] S.J. Cho, M. Kelly, K.T. Rognlien, J.A. Cho, J.K.H. Horber, B.P.
Jena, SNAREs in opposing bilayers interact in a circular array to
form conducting pores, Biophys. J. 83 (2002) 2522–2527.
[165] E.I. Pecheur, I. Martin, O. Maier, U. Bakowski, J.M. Ruysschaert,
D. Hoekstra, Phospholipid species act as modulators in p97/p47-
mediated fusion of golgi membranes, Biochemistry 41 (2002)
9813–9823.
J.A. Szule, J.R. Coorssen / Biochimica et Biophysica Acta 1641 (2003) 121–135134
[166] M.E. Haque, T.J. McIntosh, B.R. Lentz, Influence of lipid compo-
sition on physical properties and PEG-mediated fusion of curved and
uncurved model membrane vesicles: ‘‘Nature’s own’’ fusogenic lipid
bilayer, Biochemistry 40 (2001) 4340–4348.
[167] A. Bracher, J. Kadlec, H. Betz, W. Weissenhorn, X-ray structure of a
neuronal complexin-SNARE complex from squid, J. Biol. Chem.
277 (2002) 26517–26523.
[168] D.A. Archer, M.E. Graham, R.D. Burgoyne, Complexin regulates
the closure of the fusion pore during regulated vesicle exocytosis, J.
Biol. Chem. 277 (2002) 18249–18252.
[169] F. Parlati, J.A. McNew, R. Fukuda, R. Miller, T.H. Sollner, J.E.
Rothman, Topological restriction of SNARE-dependent membrane
fusion, Nature 407 (2000) 194–198.
[170] H.R.B. Pelham, SNAREs and the specificity of membrane fusion,
Trends Cell Biol. 11 (2001) 99–101.
[171] L.M. Gutierrez, S. Viniegra, J. Rueda, A.V. Ferrer-Montiel, J.M.
Canaves, M. Montal, A peptide that mimics the C-terminal sequence
of SNAP-25 inhibits secretory vesicle docking in chromaffin cells,
J. Biol. Chem. 272 (1997) 2634–2639.
[172] J.P. Apland, J.A. Biser, M. Adler, A.V. Ferrer-Montiel, M. Montal,
M.G. Filbert, Peptides that mimic the carboxy-terminal domain of
SNAP-25 block acetylcholine release at an aplysia synapse, J. Appl.
Toxicol. 19 (1999) S23–S26.
[173] M.M. Kozlov, V.S. Markin, Possible mechanism of membrane fu-
sion, Biofizika 28 (1983) 242–247.
[174] L. Chernomordik, A. Chanturiya, J. Green, J. Zimmerberg, The
hemifusion intermediate and its conversion to complete fusion:
regulation by membrane composition, Biophys. J. 69 (1995)
922–929.
[175] R.P. Rand, Interacting phospholipid bilayers: measured forces and
induced structural changes, Annu. Rev. Biophys. Bioeng. 10 (1981)
277–314.
[176] S.M. Gruner, Intrinsic curvature hypothesis for biomembrane lipid
composition: a role for non-bilayer lipids, Proc. Natl. Acad. Sci.
U. S. A. 82 (1985) 3665–3669.
[177] K. Gawrisch, V.A. Parsegian, D.A. Hajduk, M.W. Tate, S.M. Gruner,
Energetics of a hexagonal– lamellar–hexagonal-phase transition se-
quence in dioleoylphosphatidylethanolamine membranes, Biochem-
istry 31 (1992) 2856–2864.
[178] M.M. Kozlov, S. Leikin, R.P. Rand, Bending, hydration and inter-
stitial energies quantitatively account for the hexagonal– lamellar–
hexagonal reentrant phase transition in dioleoylphosphatidylethanol-
amine, Biophys. J. 67 (1994) 1603–1611.
[179] Z. Chen, R.P. Rand, Comparative study of the effects of several n-
alkanes on phospholipid hexagonal phases, Biophys. J. 74 (1998)
944–952.
[180] V. Luzzati, F. Husson, The structure of the liquid-crystalline phases
of lipid–water systems, J. Cell Biol. 12 (1962) 207–219.
[181] L. Chernomordik, M.M. Kozlov, J. Zimmerberg, Lipids in biological
membrane fusion, J. Membr. Biol. 146 (1995) 1–14.
[182] L. Yang, H.W. Huang, Observation of a membrane fusion intermedi-
ate structure, Science 297 (2002) 1877–1879.
[183] S.J. Marrink, P. Tieleman, Molecular dynamics simulation of spon-
taneous membrane fusion during a cubic–hexagonal phase transi-
tion, Biophys. J. 83 (2002) 2386–2392.
[184] L.V. Chernomordik, S.S. Vogel, A. Sokoloff, H.O. Onaran, E.A.
Leikina, J. Zimmerberg, Lysolipids reversibly inhibit Ca2 +-, GTP-
and pH-dependent fusion of biological membranes, FEBS Lett. 318
(1993) 71–76.
[185] S.S. Vogel, E.A. Leikina, L.V. Chernomordik, Lysophosphatidyl-
choline reversibly arrests exocytosis and viral fusion at a stage
between triggering and membrane merger, J. Biol. Chem. 268
(1993) 25764–25768.
[186] L.M. Johns, E.S. Levitan, E.A. Shelden, R.W. Holz, D. Axelrod,
Restriction of secretory granule motion near the plasma membrane
of chromaffin cells, J. Cell Biol. 153 (2001) 177–190.
[187] J. Pevsner, S.C. Hsu, J.E.A. Braun, N. Calakos, A.E. Ting, M.K.
Bennett, R.H. Scheller, Specificity and regulation of a synaptic
vesicle docking complex, Neuron 13 (1994) 353–361.
[188] N. Takahashi, T. Kishimoto, T. Nemoto, T. Kadowaki, H. Kasai,
Fusion pore dynamics and insulin granule exocytosis in the pancre-
atic islet, Science 297 (2002) 1349–1352.
[189] I. Bezprozvanny, R.H. Scheller, R.W. Tsien, Functional impact of
syntaxin on gating of N-type and Q-type calcium channels, Nature
378 (1995) 623–626.
[190] S. Mochida, C.T. Yokoyama, D.K. Kim, K. Itoh, W.A. Catterall,
Evidence for a voltage-dependent enhancement of neurotransmit-
ter release mediated via the synaptic protein interaction site of
N-type Ca2 + channels, Proc. Natl. Acad. Sci. U. S. A. 95 (1998)
14523–14528.
[191] W.A. Catterall, Interactions of presynaptic Ca2 + channels and
SNARE proteins in neurotransmitter release, Ann. N.Y. Acad. Sci.
868 (1999) 144–159.
[192] S.E. Jarvis, G.W. Zamponi, Interactions between presynaptic Ca2 +
channels, cytoplasmic messengers and proteins of the synaptic vesicle
release complex, Trends Pharmacol. Sci. 22 (2001) 519–522.
[193] S.E. Jarvis, G.W. Zamponi, Distinct molecular determinants govern
syntaxin1A-mediated inactivation and G-protein inhibition of N-type
calcium channels, J. Neurosci. 21 (2001) 2939–2948.
[194] E.F. Stanley, R.R. Mirotznik, Cleavage of syntaxin prevents G-pro-
tein regulation of presynaptic calcium channels, Nature 385 (1997)
340–343.
[195] J. Ji, S. Tsuk, A.M.F. Salapatek, X. Huang, D. Chikvashvili, E.A.
Pasyk, Y. Kang, L. Sheu, R. Tsushima, N. Diamant, W.S. Trimble, I.
Lotan, H.Y. Gaisano, The 25-kDa synaptosome-associated protein
(SNAP-25) binds and inhibits delayed rectifier potassium channels
in secretory cells, J. Biol. Chem. 277 (2002) 20195–20204.
[196] I. Michaelevski, D. Chikvashvili, S. Tsuk, O. Fili, M.J. Lohse, D.
Singer-Lahat, I. Lotan, Modulation of a brain voltage-gated K+ chan-
nel by syntaxin 1A requires the physical interaction of Ghg with the
channel, J. Biol. Chem. 277 (2002) 34909–34917.
[197] E. Cormet-Boyaka, A. Di, S.Y. Chang, A.P. Naren, A. Tousson, D.J.
Nelson, K.L. Kirk, CFTR chloride channels are regulated by a
SNAP-23/syntaxin 1A complex, Proc. Natl. Acad. Sci. U. S. A. 99
(2002) 12477–12482.
[198] J.D. Spafford, D.W. Munno, P. Van Nierop, Z.P. Feng, S.E. Jarvis,
W.J. Gallin, A.B. Smit, G.W. Zamponi, N.I. Syed, Calcium channel
structural determinants of synaptic transmission between identified
invertebrate neurons, J. Biol. Chem. 278 (2003) 4258–4267.
[199] O. Wiser, M. Trus, A. Hernandez, E. Renstrom, S. Barg, P. Rorsman,
D. Atlas, The voltage sensitive Lc-type Ca2 + channel is functionally
coupled to the exocytotic machinery, Proc. Natl. Acad. Sci. U. S. A.
96 (1999) 248–253.
[200] D. Atlas, O. Wiser, M. Trus, The voltage-gated Ca2 + channel is the
Ca2 + sensor of fast neurotransmitter release, Cell. Mol. Neurobiol.
21 (2001) 717–731.
[201] T. Lang, M. Margittai, H. Holzler, R. Jahn, SNAREs in native plas-
ma membranes are active and readily form core complexes with
endogenous and exogenous SNAREs, J. Cell Biol. 158 (2002)
751–760.
[202] D. Fasshauer, W. Antonin, V. Subramaniam, R. Jahn, SNARE as-
sembly and disassembly exhibit a pronounced hysteresis, Nat.
Struct. Biol. 9 (2002) 144–151.
[203] S.J. Hagan, J. Hofrichter, A. Szabo, W.A. Eaton, Diffusion-limited
contact formation in unfolded cytochrome c: estimating the maxi-
mum rate of protein folding, Proc. Natl. Acad. Sci. U. S. A. 93
(1996) 11615–11617.
[204] P. Wittung-Stafshede, J.C. Lee, J.R. Winkler, H.B. Gray, Cyto-
chrome b562 folding triggered by electron transfer: approaching
the speed limit for formation of a four-helix-bundle protein, Proc.
Natl. Acad. Sci. U. S. A. 96 (1999) 6587–6590.
[205] Y. Levy, E. Hanan, B. Solomon, O.M. Becker, Helix–coil transi-
tion of PrP106–126: molecular dynamic study, Proteins 45 (2001)
382–396.
J.A. Szule, J.R. Coorssen / Biochimica et Biophysica Acta 1641 (2003) 121–135 135
[206] D.P. Siegel, W.J. Green, Y. Talmon, The mechanisms of lamel-
lar-to-inverted hexagonal phase transitions: a study using temper-
ature-jump cryo-electron microscopy, Biophys. J. 66 (1994)
402–412.
[207] G.W. Lawrence, J.O. Dolly, Multiple forms of SNARE complexes in
exocytosis from chromaffin cells: effects of Ca2 +, MgATP and bot-
ulinum toxin type A, J. Cell Sci. 115 (2002) 667–673.
[208] S. Quetglas, C. Leveque, R. Miquelis, K. Sato, M. Seager, Ca2 +-
dependent regulation of synaptic SNARE complex assembly via a
calmodulin- and phospholipid-binding domain or synaptobrevin,
Proc. Natl. Acad. Sci. U. S. A. 97 (2000) 9695–9700.
[209] G. Palade, Intracellular aspects of the process of protein synthesis,
Science 189 (1975) 347–358.